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A stable mode of bookmarking by TBP recruits RNA Polymerase II to mitotic chromosomes
Sheila S. Teves*1, Luye An2, Aarohi Bhargava-Shah1, Lianqi Xie1, Xavier Darzacq1, Robert Tjian*1,3
1Department of Molecular and Cell Biology, Li Ka Shing Center for Biomedical and Health
Sciences, CIRM Center of Excellence, University of California, Berkeley, CA 94720, USA 2 Biochemistry, Molecular & Cell Biology, Cornell University, Ithaca, NY 14853
3Howard Hughes Medical Institute, Berkeley, CA 94720, USA
*To whom correspondence should be addressed:
Sheila S. Teves, Ph.D.
University of California, Berkeley
450 Li Ka Shing #3370, Berkeley, CA 94720-3370
Robert Tjian, Ph.D.
Howard Hughes Investigator and Professor of Biochemistry, Biophysics and Structural Biology
University of California, Berkeley
450 Li Ka Shing #3370, Berkeley, CA 94720-3370
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Abstract How a cell maintains transcriptional fidelity across the cell cycle has remained an enduring
mystery in biology. One of the challenges arises during mitosis when chromatin becomes highly
condensed and transcription is shut off. How do the new daughter cells re-establish the original
transcription program? Here, we report that the TATA-binding protein (TBP), a key component
of the core transcriptional machinery, remains bound globally to promoters of active genes in ES
cells during mitosis. Using single molecule imaging in live cells, we observed that mitotic binding
of TBP is highly stable, with an average residence time of several minutes. This stable binding
is in stark contrast to typical TFs with residence times of seconds. To test the functional effect of
mitotic TBP binding, we used a drug-inducible degron system and found that TBP binding
promotes the association of RNA Polymerase II with mitotic chromosomes, and facilitates
transcriptional reactivation following mitosis. Taken together, these results suggest that the core
transcriptional machinery maintains global transcriptional memory during mitosis.
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Introduction
Faithful maintenance of transcription programs is essential to direct cell state and identity.
However, during each cell cycle event of mammalian cells, this transcriptional fidelity is
challenged in multiple ways. First, the genome becomes highly condensed into characteristic
mitotic chromosomes (Koshland and Strunnikov, 1995). Secondly, transcription becomes
globally inhibited through cell cycle dependent phosphorylation cascades that inactivate the
transcriptional machinery (Prescott and Bender, 1962; Rhind and Russell, 2012; Taylor, 1960).
Lastly, the disassembly of the nuclear membrane combined with TF exclusion from mitotic
chromosomes was thought to result in the dispersal of most TFs throughout the cytoplasm
(Gottesfeld and Forbes, 1997; John and Workman, 1998; Martínez-Balbás et al., 1995;
Rizkallah and Hurt, 2009). How then do the new daughter cells faithfully re-establish the original
transcription program? A clue to the potential mechanism for transcriptional memory through the
cell cycle emerged when the first TF that remained bound to mitotic chromosomes was
identified (Xing et al., 2005), and a hypothesis for mitotic bookmarking was proposed (Michelotti
et al., 1997). The theory posited that a select group of privileged TFs maintain the ability to bind
to target sequences during mitosis and “bookmark” their target genes for efficient reactivation
following cell division. Recently, we discovered that previous evidence for the widely observed
exclusion of TFs from mitotic chromosomes was an artifact of chemical crosslinking-based cell
fixation prior to imaging, e.g., formaldehyde crosslinking (Teves et al., 2016). By relying on live
cell imaging, our studies indicated that in fact most TFs remain associated with mitotic
chromosomes but in a dynamic manner. Rather than acting as a stable bookmark, sequence-
specific TFs seem to ‘hover’ on mitotic chromosomes in general. However, it was not clear how
such a dynamic mode of bookmarking by TFs could maintain stable transcriptional memory
during mitosis.
In order to effect transcriptional regulation, sequence-specific TFs at enhancers must cross-talk
with the RNA Polymerase II (Pol II) machinery at promoters. Indeed, previous studies have
shown that promoters and transcription start sites (TSSs) of certain genes remain sensitive to
permanganate oxidation during mitosis (Michelotti et al., 1997), providing indirect evidence for
potential promoter-specific bookmarking factors that maintain an open chromatin conformation
at these chromosomal locations. Central to the recruitment of Pol II to promoters is the TATA-
binding protein (TBP), the prototypic member of the multi-subunit core promoter recognition
ensemble TFIID (Goodrich and Tjian, 1994). At most eukaryotic promoters, TBP and its
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associated factors (TAFs) are the first components of the pre-initiation complex (PIC) to bind
promoters of active genes in a stepwise assembly of the general TFs and Pol II. An essential
protein, TBP forms extensive contacts with promoter DNA by introducing sharp kinks that
results in an almost 90° bend in the double helix, which leads to partial DNA unwinding and
subsequent widening of the minor groove for maximum TBP contact (Kim et al., 1993; Louder et
al., 2016; Martianov et al., 2002). TBP also plays a crucial role in the hierarchical assembly of
the transcriptional machinery (Zhang et al., 2016), and in the positioning of promoter DNA into
the Pol II binding site (He et al., 2016; Plaschka et al., 2016). These essential functions at the
promoter make TBP an attractive candidate for a global facilitator of transcriptional memory. In
order for TBP to be considered a global bookmarker of active genes, TBP must (1) bind to
promoters of active genes during mitosis, and (2) promote efficient transcriptional reactivation
following mitosis.
Over time, a number of studies have tested the hypothesis of TBP as a mitotic bookmarker, but
results have been conflicting. For instance, immunofluorescence (IF) staining of TFIID subunits,
including TBP, showed cellular redistribution of the subunits away from chromosomes during
mitosis (Segil et al., 1996), while live-cell imaging of GFP-tagged but over-expressed TBP
shows enrichment on chromosomes throughout mitosis (Chen et al., 2002). We now know,
however, that these conclusions need to be revisited, as these early studies suffered from
previously unrecognized experimental artifacts, including the formaldehyde crosslinking artifact
we recently uncovered (Teves et al., 2016), as well as over-expression biases for proteins with
highly regulated concentrations within the cell (Um et al., 2001). Furthermore, some studies
have found that TBP remains bound at specific loci during mitosis via chromatin
immunoprecipitation (Xing et al., 2008), whereas others have not (Kelly et al., 2010). These
conflicting results suggest that the question of whether TBP bookmarks active gene promoters
remains unresolved. Moreover, the functional consequence of TBP bookmarking (i.e. promoting
transcriptional memory through mitosis), if any, has thus far not been established.
Through live-cell imaging of endogenously tagged proteins, we report that TBP stably binds to
chromatin for minutes in contrast to most sequence-specific TFs studied thus far that bind on
the order of seconds. Moreover, TBP remains stably associated with mitotic chromosomes, and
such stable binding is also in contrast to the more dynamic mode of studied sequence-specific
TF association with mitotic chromosomes (Teves et al., 2016). TBP stable binding occurs on a
global scale at promoters of active genes during mitosis. We dissected the functional
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consequence of TBP binding during mitosis by using a drug inducible protein degradation
system and found that TBP recruits a small fraction of Pol II molecules to mitotic chromosomes.
Lastly, nascent RNA analysis indicates that TBP promotes efficient reactivation of global ES cell
transcription program following mitosis. TBP, therefore, is unique among the TFs we have
studied thus far, as it appears to stably bookmark active genes during mitosis and thereby
maintain transcriptional memory across the cell cycle.
Results
TBP bookmarks mitotic chromosomes of mouse ES cells
A previous study has shown that DNase I hypersensitive sites at promoters are maintained
during mitosis in murine erythroblast cells (Hsiung et al., 2015). Similarly, we have found that
mitotic chromosomes of mouse ES cells remain as accessible to Tn5 transposase insertion as
interphase chromatin (Teves et al., 2016). To examine chromatin accessibility specifically at the
TSS of mouse ES cells, we analyzed our previously published ATAC-seq data at the TSS of all
genes. Reads under 100 bp indicate potential transcription factor (TF) binding sites, and these
sites are highly enriched at the TSS of all active genes in asynchronous cells (Figure 1A).
Notably, these reads remain nearly equally enriched at the TSS of active genes during mitosis
(Figure 1A) and the level of enrichment remains proportional to expression levels as seen by
heatmap analysis. When we averaged the signal across all genes, we observed that the ATAC-
seq signal at the TSS in mitosis is about 91% of the signal in asynchronous cells (Figure 1A,
bottom). Furthermore, when we performed unbiased k-means clustering, we do not observe any
population differing between the two samples (Supplemental Figure 1), suggesting high
concordance in accessibility at the TSS between asynchronous and mitotic cells. Enrichment of
short fragments by ATAC-seq at a given locus is indicative of TF binding. Such maintenance of
accessibility at the TSS suggests that the TSS of active genes may be bookmarked by TFs
throughout mitosis. We also analyzed the mono-nucleosome sized fragments (180 — 250 bp)
from the ATAC-seq at the TSS genome-wide. Remarkably, we found that the accessibility of the
nucleosomes flanking the TSS increased during mitosis relative to interphase chromatin (Figure
1B). When we averaged the signal for all genes, we observed a 15% increase in signal in
mitotic cells (Figure 1B, bottom). Furthermore, unbiased k-means clustering showed that, while
some variation between clusters exist, mitotic signal is consistently higher than the
asynchronous signal (Supplemental Figure 2). These results suggest that nucleosomes around
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the TSS may have a more open and accessible configuration during mitosis than in interphase,
despite the general inhibition of transcription observed in mitosis (Prescott and Bender, 1962).
Given the persistence of chromatin accessibility at promoters of mitotic mouse ES cells, we
hypothesized that the transcriptional machinery assembled at the TSS may remain associated
during mitosis. TBP, a core member of the transcriptional machinery, has previously been
shown to associate with certain loci during mitosis (Xing et al., 2008). Thus, we hypothesized
that TBP may act as a general bookmarking factor for active genes during mitosis in mouse ES
cells. We therefore set out to visualize TBP dynamics throughout the cell cycle. In order to
circumvent artifacts caused by cell fixation and over-expression, we used CRISPR/Cas9 to
knock-in HaloTag at the endogenous TBP locus and allow for live-cell imaging. We generated
several cell lines containing heterozygous and homozygous tagged Halo-TBP, as determined by
Western blot (Figure 1C). TBP is an essential gene, and so the ability of the homozygous Halo-
TBP ES cell line to generate all three germ layers in a teratoma assay assured us that
pluripotency is maintained, and that tagged TBP is functioning normally (Supplemental Figure
3). After stable integration of H2B-GFP in the Halo-TBP C41 homozygous line, we performed
two-color time-lapse imaging of H2B-GFP and Halo-TBP as mouse ES cells undergo mitosis.
We found that the endogenous Halo-TBP is enriched on mitotic chromosomes throughout
mitosis (Figure 1D).
Several studies have previously reported that concentrations of TBP within the cell are highly
regulated (Li et al., 2015; Um et al., 2001), which questions previous experiments examining the
dynamics of TBP association with mitotic chromosomes using over-expressed fluorescently-
tagged proteins. We thus tested whether over-expressed Halo-TBP could recapitulate the
behavior of endogenous Halo-TBP by comparing the C41 knock-in line with a stable cell line
containing exogenous over-expressed Halo-TBP. We analyzed the enrichment on mitotic
chromosomes of the over-expressed (Halo-TBP OE) and the endogenous knock-in (Halo-TBP
KI) in live versus fixed cells as previously described (Teves et al., 2016). We found that Halo-
TBP OE cells showed the artifactual exclusion from mitotic chromosomes following
formaldehyde fixation whereas the knock-in cells maintained enrichment even after fixation
(Figure 1E,F). These results suggest that, unlike most sequence specific TFs that are
susceptible to fixation-induced artifacts, the endogenous TBP does not become evicted from
mitotic chromosomes after fixation, suggesting a distinct interaction modality. In contrast, over-
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expressed exogenous TBP is susceptible to fixation-induced artifacts and therefore does not
faithfully recapitulate the endogenous behavior.
TBP stably binds to mitotic chromosomes
We next asked how TBP interaction with mitotic chromosomes compares to its interaction with
interphase chromatin. We imaged individual Halo-TBP molecules at a high camera speed (133
Hz) and high illumination intensity using stroboscopic photoactivatable single particle tracking
(spaSPT) in order to simultaneously track both fast-diffusing and chromatin-bound molecules
(Hansen et al., 2017, 2018). We then localized individual particles and measured their
displacement between consecutive frames (Supplemental Figure 4). Figure 2A shows the
distribution of displacements after 3 frames (Dt = 22.5 ms) for cells in interphase and in mitosis.
The shift to longer displacements in mitosis compared to interphase suggests a difference in the
bound fraction and/or the diffusion constant between the two cell cycle stages. This difference
becomes more apparent when the cumulative distribution function (CDF) is plotted for
displacements after 3 frames (Dt = 22.5 ms) for both interphase and mitotic cells (Figure 2B),
which shows a rightward shift in the CDF for mitotic cells. We then used SPOT-ON, an analysis
tool for kinetic modeling of SPT data, and fitted the distribution of displacements with a 2-state
kinetic model representing ‘bound’ and ‘free’ populations (Figure 2C) (Hansen et al., 2018).
Such a model gives estimates of the fraction of molecules in each state, and the corresponding
apparent diffusion constants for each population.
The resulting fit for the 2-state model shows that the fraction of bound TBP decreases by half,
from 34.6% in interphase to 18.6% in mitosis (Table 1). However, upon closer inspection, we
find that the 2-state model fitted the data poorly, showing large residuals after the fit
(Supplemental Figure 5). This result suggests that a dual classification of ‘bound’ and ‘free’ TBP
populations may be insufficient to accurately characterize the data. Therefore, we fitted a 3-
state kinetic model to represent three distinct populations: a fast-diffusing TBP population
(‘fast’), a slower diffusing population wherein TBP may be diffusing in a complex with the TAFs
as TFIID (‘slow’), and a stably DNA bound population (‘bound’) (Figure 2C). The 3-state model
fitted the data more precisely (Figure 2A, black line), showing reduced residuals after fitting
(Supplemental Figure 5 and 6). From this analysis, we estimate that in interphase 38% of TBP
molecules are in fast diffusion mode, whereas 37.2% are found in a slower 3D diffusing complex
(Table 1). Relatedly, we find that 24.8% of TBP molecules are bound to interphase chromatin
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(Table 1). During mitosis, the chromatin bound fraction decreases to 12.3%, with concomitant
increases in both the slow and fast diffusing populations (46.5% and 41.2%, respectively) (Table
1). This decrease in fraction bound during mitosis may reflect the minimum amount of TBP
needed to ‘bookmark’ active genes during mitosis. Furthermore, measured diffusion constants
for TBP molecules that are in fast (Apparent Dfast) or in slow diffusion (Apparent Dslow) show no
significant difference between interphase and mitotic cells (Table 1), suggesting that although
the fraction of TBP in each subpopulation is different in mitosis, the diffusion of each
subpopulation remains the same.
Given the decreased percent of TBP molecules that are bound during mitosis, we next asked
how stable is TBP binding and if the mitotic binding dynamics differ from those of the bound
population in interphase. We previously discovered that prototypic sequence-specific TFs such
as Sox2 display a more dynamic binding behavior during mitosis compared to interphase,
showing about 50% decrease in residence time during mitosis that is largely due to the global
decrease in transcriptional activity (Teves et al., 2016). To determine if bound TBP molecules
behave similarly to sequence-specific TFs, we performed single particle tracking (SPT) with long
exposure times (500 ms) as previously described (Watanabe and Mitchison, 2002). This
imaging technique allows for a ‘blurring out’ of diffusing molecules while bound ones appear as
diffraction-limited spots. After localization and tracking of individual bound molecules, we
measured the dwell time, the amount of time each molecule remains detected, and plotted the
log-log histogram of dwell times for interphase and mitotic cells (Figure 2D). In contrast to
sequence-specific TFs like Sox2, TBP remains as stably bound on mitotic chromosomes as on
interphase chromatin. We then fitted a two-component exponential decay model, representing
specific versus non-specific binding events, to the dwell time histograms and extracted
residence times for the two bound populations (Chen et al., 2014). After correcting for
photobleaching, the residence time for specific Halo-TBP binding during interphase is on the
order of minutes (Figure 2E). This binding is significantly more stable than typical sequence-
specific TFs like Sox2, p53, GR, which normally have residence times on the order of a few to
around ten seconds in interphase (Chen et al., 2014; Mazza et al., 2012; Mueller et al., 2008;
Normanno et al., 2015; Swinstead et al., 2016). Surprisingly, some Halo-TBP also remains
stably bound during mitosis (Figure 2E), with a calculated average residence time of 118
seconds. This apparent TBP residence time in mitosis is even longer than in interphase.
However, based on the dwell time histogram, this is likely due to the contribution of a small
fraction of TBP molecules (less than 1%) that appear very stably bound (dwell time above 100 s
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in Figure 2D). Given that the whole distribution profiles appear very similar, we concluded that
for most of the bound TBP, residence times are indistinguishable between interphase and
mitotic cells. This result is in stark contrast to Sox2, whose residence time decreases by at least
half during mitosis, suggesting that TBP binding to mitotic chromosomes may be independent of
transcriptional activity.
As an orthogonal approach to SPT, we performed FRAP (Fluorescence Recovery after
Photobleaching) analysis to independently measure TBP binding dynamics during interphase
and mitosis. We plotted the FRAP recovery at the bleach spot over time for Halo-TBP in
interphase and in mitotic cells, along with Halo-3xNLS and H2B-Halo (Figure 2F). When
normalized for bleach depth, the recovery curves for interphase and mitotic cells become super-
imposable (Figure 2G). The difference in bleach depth may indicate a difference in the fraction
of bound molecules between interphase and mitotic cells, which would be consistent with our
SPT results (Table 1; 24.8% vs. 12.3% bound in interphase and mitosis, respectively), whereas
the super-imposable recovery curves would be consistent with similar residence times of the
bound fraction. This analysis underscores the need for multiple orthogonal measurements to
better interpret TF dynamics.
TBP binds to the TSS of active genes in mitosis
We next asked whether TBP binds to specific sites in the genome during mitosis. Given the
relatively stable binding of TBP during mitosis and its resistance to the formaldehyde-based
exclusion artifact, we reasoned that endogenous TBP could be amenable to formaldehyde-
based ChIP-seq analysis without complications from incurring cross-linking artifacts. Indeed we
were able to perform ChIP-seq on both asynchronous and mitotic cells in two biological
replicates that are highly reproducible (Supplemental Figure 7). Genome browser visualization
of mapped reads for each replicate shows that binding profiles are highly reproducible, and that
TBP is maintained at the same genomic sites in mitosis as in interphase chromatin (Figure 3A).
We next analyzed the level of TBP enrichment at the TSS of all genes and displayed the ChIP-
seq signal on a 4 kb region centered at the TSS as a heatmap, with genes arranged by
decreasing expression in the asynchronous population (Figure 3B). The heat map shows that
TBP enrichment at the TSS is correlated with expression level both in the asynchronous and
mitotic population. Averaging the enrichment across all TSSs shows that enrichment in mitosis
is roughly 80% of the enrichment in asynchronous cells (Figure 3C). This reduced enrichment at
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the TSS during mitosis likely reflects the reduced fraction of molecules that are bound during
mitosis rather than the strength of binding (Figure 2C). To determine whether TBP binds more
to certain classes of genes in mitosis, we performed unbiased k-means clustering with k = 6 and
displayed the clusters as heatmaps centered at the TSS (Figure 3D). This clustering analysis
shows 3 main groups. Group 1 includes the first 2 clusters, which show increased TBP binding
in mitosis relative to asynchronous cells. Group 2 consists of genes that display no change or
very little TBP signal at the TSS. Lastly, group 3 is composed of the last three clusters that show
decreased TBP signal in mitosis. This analysis suggests that TBP binds differentially to specific
genes depending on cell cycle phase. However, when we analyzed the types of genes within
each group using gene ontology (GO) term analysis, we find that groups 1 and 3 are enriched
for similar classes of genes, primarily ones involved in the cell cycle (Figure 3E). This analysis
suggests that the differences in TBP binding that we observe by ChIP-seq largely reflect the
cyclical expression of genes during the cell cycle. Despite the variations in TBP levels, most
active genes retain TBP binding in mitosis, suggesting a global bookmarking activity by TBP.
TBP recruits RNA Polymerase II to mitotic chromosomes
Having determined that TBP stably binds to the TSS of active genes during mitosis, we next
asked what is the function of such stable TBP mitotic binding. To address this question, we
endogenously knocked-in the plant-specific minimal auxin-inducible degron (mAID) (Holland et
al., 2012; Nishimura et al., 2009) at the TBP locus to generate homozygous mAID-TBP fusion
proteins (C94 cell line). This fusion enables acute, auxin-inducible degradation of the mAID-
tagged TBP via the ubiquitin degradation pathway (Figure 4A). In fact, within 6 hours of IAA
(auxin) treatment, only about 3% of mAID-TBP molecules remains detectable by bulk protein
analysis with Western blot (Figure 4B), and by immunofluorescence using a-TBP antibody
(Figure 4C). This drug-inducible degradation of TBP provides us with a robust tool to causally
test the functions of TBP binding specifically during mitosis.
A primary function of TBP at the TSS of active genes is to recruit Pol II and form the pre-
initiation complex (PIC) (Goodrich and Tjian, 1994; Kuras and Struhl, 1999). Our discovery here
of stable TBP binding at TSSs during mitosis led us to hypothesize that TBP may function
similarly during mitosis and recruit Pol II to active genes, despite the extensive decrease in
global transcriptional activity. To test this hypothesis, we endogenously knocked-in a HaloTag at
the Rpb1 locus, the catalytic subunit of RNA Polymerase II, in the mAID-TBP (C94) cells. We
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successfully produced heterozygous knock-in of Halo-Pol2 II, as shown by Western blot
analysis (Figure 4D), and the tagged protein localizes within the nucleus as expected (Figure
4E). We further assessed the functionality of the tagged Pol II with several experiments. First,
we used spaSPT to analyze the distribution of Pol II displacements before and after
transcription inhibition by Flavopiridol (elongation inhibitor) and Triptolide (initiation inhibitor)
(Figure 4F). We found that Halo-Pol II showed a significant shift in displacements towards
longer jumps, indicative of increased diffusing molecules and decreased bound ones. When
fitting the data with a 2-state model, we found that the fraction of bound Pol II decreased by
80% after drug treatments (Figure 4G). These results suggest that the halo-tagged Pol II is
sensitive to drug inhibition. Furthermore, ChIP-qPCR analysis using antibodies against Pol II
(targeting total Pol II) and Flag (located between Halo and the N-terminal of Rpb1, targeting only
Halo-Pol II) showed that the tagged Pol II binds to regions where the endogenous Pol II binds
(Supplemental Figure 8), altogether confirming that the tagged Pol II remains functional.
To test the role of TBP in recruiting Pol II, we next performed spaSPT on Halo-Pol II in
interphase and mitosis, with and without TBP. The distribution of Halo-Pol II displacements
shows an increase in longer displacements between consecutive frames after TBP degradation
both in interphase and mitotic cells (Supplemental Figure 9). This effect is evident in the
rightward shift of the displacement CDF after TBP degradation for both interphase and mitotic
cells (Figure 5A). We then fitted a 2-state kinetic model as before to represent ‘bound’ and ‘free’
populations (Figure 2C) and extracted estimates of the fraction of molecules and corresponding
diffusion constants for each population (Table 2). However, as we had found with TBP, the 2-
state kinetic model fitted the Pol II data poorly, particularly for mitotic cells, as evident by the
large residuals after fitting (Supplemental Figure 10-13), suggesting that this model is
insufficient to characterize Pol II dynamics. We then fitted a 3-state kinetic model
(Supplementary Figure 4) and extracted the fraction of Halo-Pol II molecules in each state for all
the tested conditions (Table 2). We note that despite differences in absolute numbers, the global
trend remains similar in extracted parameters between the 2-state and 3-state models, and so
conclusions remain the same.
During interphase, 32% of Pol II is fast diffusing whereas 45.6% is slow diffusing. The nature or
composition of the two distinctly diffusing population remains unknown, but what is clear is that
the fraction of Pol II that is bound on chromatin is 22.4%. This bound population decreases by
half to 12.1% during mitosis, revealing a small but significant population of Pol II that persists on
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mitotic chromosomes. We next focused on the effect of TBP degradation on Pol II recruitment
and binding. Upon TBP degradation in interphase cells, the fraction of bound Halo-Pol II
decreases from 22.4% to 16.1% (Table 2), consistent with the important role of TBP in recruiting
Pol II to active genes. TBP degradation during mitosis also led to a decrease in the fraction of
bound Pol II, from 12.1% in untreated mitotic cells to about 10.8% after TBP degradation. These
results suggest that TBP recruitment of Pol II to DNA is independent of the cell cycle or the
chromatin condensation state.
We next examined the dynamics of Pol II binding to mitotic chromosomes by performing SPT
with long exposure times (500 ms). We measured the dwell time of diffraction-limited bound
molecules and plotted the log-log histogram of dwell times for Halo-Pol II in interphase and
mitosis with and without TBP (Figure 5B). The most obvious difference is seen between
interphase and mitotic cells, with much reduced dwell times of Halo-Pol II during mitosis
compared to interphase cells. This decrease is consistent with the global decrease in active
transcription during mitosis. After degrading TBP, Halo-Pol II shows decreased dwell time in
interphase, consistent with the role of TBP in initiating transcription. In contrast, TBP
degradation shows less effect on the dwell time of Pol II during mitosis. We then fitted a two-
state exponential decay model to the dwell times to extract the apparent koff of Pol II specific
binding. Pol II binding to DNA involves complex steps, from transient binding due to promoter
association and abortive initiation, to the stable binding during elongation, and to the as yet
undefined mechanisms for termination. Therefore, modeling the binding of Pol II to DNA using a
single residence time likely over-simplifies the complex dynamics of Pol II progression during
transcription. With this caution in mind, instead of extracting a residence time for Pol II, we
calculated the apparent half-life of the bound population. During interphase, the apparent half-
life of Pol II is 26.7 seconds (Figure 5C). TBP degradation leads to a modest decrease in
apparent half-life, to 21.0 seconds. This modest decrease is consistent with the prominent role
of TBP in promoter association, which is largely composed of transient Pol II binding. During
mitosis, the apparent half-life of Pol II binding decreases to 3.5 seconds. This order of
magnitude decrease in apparent half-life suggests that the mechanisms that stabilize Pol II
binding becomes dramatically decreased during mitosis. Furthermore, after TBP degradation
during mitosis, the apparent half-life decreases from 3.5 to 2.3 seconds, consistent with the role
of TBP in recruiting transiently-binding Pol II to mitotic chromosomes.
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To cross-validate the SPT residence time analysis, we performed FRAP analysis on Halo-Pol II
during interphase and mitosis, with and without TBP degradation. We plotted the FRAP
recovery over time (Figure 5D) and measured the time it takes to reach 90% recovery (T90%)
(Figure 5E). As with the SPT, the most drastic difference in the FRAP curves is seen between
interphase and mitotic cells under normal TBP levels. Halo-Pol II takes 179 seconds to reach
90% recovery in interphase cells, whereas in mitosis, it takes 3 seconds. Upon TBP degradation
in interphase cells, T90% decreases to 150 seconds, consistent with the decreased apparent
half-life as measured by SPT. TBP degradation in mitotic cells shows little change in the
recovery curve relative to untreated mitotic cells, further confirming our SPT residence time
analysis. Taken together with the SPT results, these findings suggest that TBP affects the more
transient promoter association of Pol II during interphase, and potentially directs Pol II binding to
mitotic chromosomes.
Mitotic TBP binding affects the rate of transcriptional reactivation
We next asked how TBP binding during mitosis affects transcription reactivation following cell
division. Having shown that TBP promotes Pol II recruitment to mitotic chromosomes, we
hypothesized that this recruitment helps prime active genes for efficient reactivation following
mitosis. To test this hypothesis, we performed two orthogonal experiments, one based on
imaging of single cells, and another based on sequencing newly transcribed RNA products as a
time course after mitosis. First, we returned to our Halo-Pol II C64 cells and performed spaSPT.
We marked cells at the metaphase stage of mitosis and imaged the same cells every 15
minutes until 60 minutes after first staging, following cells as they exited mitosis and entered G1.
To ensure that repeated imaging had no significant effect on Pol II behavior, we performed the
same imaging regimen on various interphase cells and calculated the fraction of molecules
bound over time. This population of Pol II remained stable over the course of the imaging
regimen even for cells treated with auxin for TBP degradation, suggesting that repeated imaging
did not adversely affect Pol II behavior (Figure 6A). As expected, during the progression from
mitosis into G1, the fraction of bound Pol II molecules steadily increased over time, consistent
with increasing activation of transcription following mitosis (Figure 6B). When we performed the
same experiment with cells depleted of TBP, we observed that the fraction of bound Pol II
remained flat over time (Figure 6B), suggesting that TBP is required for re-establishing the
transcription program following mitosis.
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We also performed a global analysis of newly transcribed RNA as a function of time following
mitosis. To assess changes in newly transcribed RNA, we performed successive biochemical
fractionation and extracted the nascent chromatin-associated RNA (chr-RNA) of asynchronous
cells (A), mitotic cells synchronized with Nocodazole (M), and 30 min and 60 min after
Nocodazole release (M30 and M60, respectively) of synchronized mitotic cells in two replicates
(Figure 6C). We then performed strand-specific sequencing of the extracted chr-RNA along with
ERCC spike-in controls and mapped the reads to the mouse genome (Supplemental Figure 14
and 15). A snapshot of the mapped reads on a housekeeping gene (Gapdh) and an ES cell-
specific gene (Nanog) is shown on Figure 6D. The high proportion of sequenced reads in
intronic regions in asynchronous samples (Figure 6D, Supplemental Figure 14) confirms
successful enrichment for newly synthesized RNAs. To assess transcriptional activity through
mitosis on a global scale, we averaged the normalized signal in a 4 kb region surrounding the
TSS for all genes in each sample (Figure 6E). Overall levels decrease in Nocodazole-arrested
M samples and remain low 30 minutes after release. However, by 60 minutes after release,
RNA levels have increased to the levels in asynchronous samples. These data are consistent
with the global decrease in transcriptional activity followed by reactivation as cells exit mitosis.
To examine the role of TBP in promoting efficient reactivation, we degraded TBP in
asynchronous samples (A) and in Nocodazole arrested mitotic cells (M), and collected cells
after 30 or 60 minutes after mitosis as before (Figure 6C, Supplemental Figure 14). As with
untreated samples, we extracted and sequenced the chr-RNA and ERCC spike-in controls in a
strand-specific manner (Supplemental Figure 14 and 15). A snapshot of the mapped reads of
TBP-degraded samples on Gapdh and Nanog is also shown on Figure 6D. We still observe high
levels of intronic reads in asynchronous (A) samples, despite near complete degradation of
TBP. Our results are reminiscent of a previous study that has observed Pol II transcription in the
absence of TBP in mouse blastocyst cells (Martianov et al., 2002). However, we observe a
marked decrease in transcription reactivation in M60 samples following TBP degradation in
mitosis (Figure 6D). This decrease occurs globally as most genes show decreased nascent chr-
RNA levels (Figure 6F), suggesting a specific role for TBP in transcriptional reactivation
following mitosis.
We next examined the kinetics of transcriptional reactivation following mitosis by taking the log2
ratio of reads in the 30- and 60-minute conditions relative to mitotically arrested (M30/M and
M60/M, respectively), for both untreated and TBP-degraded samples. In this way, we can
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observe the change in RNA levels relative to mitotic cells as a function of time after release from
mitosis. Globally, the untreated M30/M sample shows no overall change in RNA levels whereas
M60/M samples show massive increase in both upstream and downstream transcription at the
TSS (Supplemental figure 16). On the other end, TBP-degraded samples show delayed
transcription levels evident in the M60/M sample (Supplemental figure 16). To determine
whether certain groups of genes behave differently from the global mean, we performed
unbiased k-means clustering on the untreated M30/M data with k = 3. Cluster 1 includes 5504
genes that show a mild increase in transcription whereas cluster 3 includes 6693 genes that
show a mild decrease in transcription relative to mitotic cells. The remaining genes (cluster 2)
show no change in transcription (Figure 7A,B). Ordering the M60/M data using the same three
clusters shows that cluster 1 increases in transcription the earliest and the fastest whereas
clusters 2 and 3 lag behind. We then ordered the M30/M and M60/M data from TBP-degraded
samples (Figure A,B). This analysis shows that the early changes in transcription seen in
untreated samples are dampened in TBP-degraded samples. Furthermore, TBP degradation
has the biggest effect on cluster 1. Using gene ontology (GO) term analysis, we find that cluster
1 is enriched for genes involved in metabolism of RNA, cell cycle, and transcription factor
activity (Figure 7C). These genes are also generally highly expressed in the asynchronous
population (Supplemental Figure 16), suggesting that these genes represent the global
transcription program of the cells. In contrast, cluster 3 is enriched for genes involved in basic
cellular processes such as microtubule cytoskeleton organization and regulation of GTPase
activity, but also for genes involved in differentiation and development such as cell
morphogenesis in differentiation, and morphogenesis of epithelium (Figure 7C). Furthermore,
these genes tend to be less expressed than cluster 1 in the asynchronous population
(Supplemental Figure 16). These data strongly suggest that TBP promotes efficient reactivation
of the global ES cell transcription program and thus plays a functional role in promoting the
maintenance of cell state through the cell cycle.
Discussion
Although different mechanisms exist to ensure faithful transmission of transcription programs
from mother to daughter cells afer mitosis, the precise role of transcription factors in this
process has remained elusive. In this study, we have shown that unlike most classical
transcription factors that bind with rapid dynamics, the endogenous TBP maintains stable
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binding at the TSS of active genes in mitotic mouse ES cells. Remarkably, such stable TBP
binding leads to recruitment of Pol II to mitotic chromosomes, despite the general inhibition of
transcriptional activity. Rather, as cells exit mitosis, TBP promotes efficient reactivation of
transcription globally by priming the promoters of active genes. Taken together, TBP acts as a
stable bookmarker of active promoters throughout mitosis and promotes transcriptional fidelity
from mother to daughter ES cells to maintain the ES cell identity.
Previous biochemical and structural data have generated static views of molecular processes,
such as the formation of stable complexes or binding of factors to DNA. These static views have
propagated the sense of stability. For instance, a ChIP signal for TFs has generally been viewed
as a binary classification of specific loci: bound or unbound. The advent of live cell single
molecule imaging has revolutionized our understanding of basic molecular processes,
particularly, how dynamic these processes are. Many TFs examined by live cell single-molecule
imaging have shown much shorter residence times on DNA than previously expected from
biochemical data. For instance, Bicoid binds to the Drosophila genome for about 100 ms (Mir et
al., 2017), p53 has an average residence time of 3-6 seconds (Loffreda et al., 2017), and Sox2
binds to specific loci in mouse ES cells for about 12 seconds on average (Chen et al., 2014;
Teves et al., 2016). Rather than a binary classification, we now have a much more dynamic
view of repeated and rapid binding/unbinding events that ultimately affect transcriptional output.
In contrast to most sequence-specific TFs, TBP seems unusual by binding to loci on the order of
minutes. Although still more dynamic than previous biochemical data had suggested, this more
stable mode of TBP binding may serve a specific function unique to TBP among TFs, perhaps
as a more stable landing pad for the dynamic binding of various other factors that make up the
transcriptional machinery. For instance, binding of both TFIIA and TFIIB are highly dependent
on prior TFIID/TBP binding, and TFIIB has been shown to bind to TBP-bound promoter DNA in
a highly transient manner through in vitro single molecule imaging (Zhang et al., 2016). Despite
the general silencing of transcription during mitosis, this relatively stable binding of TBP is
maintained, also in contrast to other sequence-specific TFs. Here we have shown that TBP
recruits Pol II to mitotic chromosomes and promotes efficient reactivation of transcription
following mitosis, but such stable binding in mitosis may also serve other functions. One
potential alternative function may be to help maintain the unique chromatin architecture of
promoters in condensed mitotic chromosomes perhaps through its stable binding or through as
yet unidentified pathways. In this way, TBP may promote transcriptional fidelity through mitosis
in multiple ways.
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A previous study has shown that blastocyst cells from mouse embryos with homozygous
deletion of the TBP locus still contain Pol II in active phosphorylation states, suggesting active
transcription in the absence of TBP (Martianov et al., 2002). Instead, the authors found that
transcription from Pol I and Pol III are dramatically reduced without TBP, suggesting a
differential dependency of the various polymerases on TBP. In this study, we have used a rapid
drug-inducible depletion of TBP and measured the newly transcribed RNA after depletion. We
have confirmed that transcription occurs even in the absence of TBP (Figure 6D). How does
transcription occur in the absence of TBP? Several mechanisms may potentially answer this
question. First, TBP-like factor (TLF, also known as TBP-related factor 2 – TRF2), a closely
related protein to TBP containing a similar saddle-like core domain for DNA binding, has been
proposed to substitute for TBP in certain specialized cases (Akhtar and Veenstra, 2011;
Dantonel et al., 1999). However, unlike the constant expression of TBP, previous studies have
shown that TLF is not expressed in early mouse embryogenesis (Martianov et al., 2001, 2002).
A second potential mechanism for TBP-independent transcription is that a TFIID complex
lacking TBP can form and activate transcription, which has been shown in vitro (Tora et al.,
1998). A third potential mechanism, and not mutually exclusive with the first two, is that
independent mechanisms exist for the initiation of transcription and the subsequent re-initiation.
Our finding that TBP depletion strongly inhibits re-activation of genes following mitosis is
consistent with this theory. That is, the first transcription event following mitosis requires TBP,
providing a rationale for TBP mitotic bookmarking, whereas subsequent transcription events
throughout interphase may occur even in the absence of TBP.
Our observation that TBP recruits Pol II to mitotic chromosomes may seem surprising, given
that historically, transcription has been shown to be globally shut-off during mitosis (Prescott
and Bender, 1962). Recent studies, however, are beginning to shed some nuance to this
historical adage. For instance, several groups have shown that transcription transiently spikes at
the later stages of mitosis, followed by an adjustment back to normal interphase levels (Hsiung
et al., 2016; Vaňková Hausnerová and Lanctôt, 2017). One potential mechanism for such a
spike in transcriptional activity could derive from our observed recruitment of Pol II by TBP to
mitotic chromosomes. Combined with the lack of crosstalk between enhancers and promoters
during mitosis (Hsiung et al., 2015), it is possible that Pol II recruitment results in promiscuous
transcriptional activation of most accessible promoters immediately following mitosis. Adding
more nuance, several groups have recently shown that certain genes remain expressed albeit
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at low levels during mitosis (Liang et al., 2015; Palozola et al., 2017). It is possible that the small
fraction of Pol II that we observe to be recruited to mitotic chromosomes is transcriptionally
active. If so, this activity must be quite transient, as we observe no detectable Pol II molecules
that bind to mitotic chromosomes for longer than 30 seconds (Figure 5C) by slow tracking SPT.
In contrast, we observe much longer residence times of Pol II during interphase when
transcription is highly active. Indeed, less than 1% of mitotically bound Pol II molecules show
binding for greater than 10 seconds (Figure 5B), which may reflect the low transcriptional
activity during mitosis as previously reported (Liang et al., 2015; Palozola et al., 2017). What
does become evident, however, is the gradual increase in bound Pol II concomitant with
increase in newly transcribed RNA as cells progress from mitosis, and the important role of TBP
in this process (Figure 6). Regardless of the transcriptional activity of Pol II during mitosis per
se, TBP promotes efficient reactivation of global transcription following mitosis, which is
necessary for faithful transmission of transcription programs through the cell cycle.
Materials and Methods
Cell culture
For all experiments, we used the mouse ES cell line JM8.N4 (RRID: CVCL_J962) obtained from
the KOMP repository (https://www.komp.org/pdf.php?cloneID=8669) and tested negative for
mycoplasma. ES cells were cultured on gelatin-coated plates in ESC media Knockout D-MEM
(Invitrogen, Waltham, MA) with 15% FBS, 0.1 mM MEMnon-essential amino acids, 2 mM
GlutaMAX, 0.1 mM 2-mercaptoethanol (Sigma) and 1000 units/ml of ESGRO (Chem- icon). ES
cells are fed daily and passaged every two days by trypsinization. Mitotic cells were
synchronized by adding 100 ng/mL of Nocodazole for 6 hr followed by shake-off. For
endogenously-tagged mAID-TBP cells, TBP degradation was performed by addition of indole-3-
acetic acid (IAA) at 500 µM final concentration for 6 hours.
Cas9-mediated endogenous knock-ins
Cas9-mediated endogenous knock-ins were performed as previously described (Teves et al.,
2016). Briefly, mouse ES cells were transfected with 0.5 µg of the Cas9 vector (containing the
specific guide RNA and the Venus coding sequence) and with 1 µg of the donor repair vector
using Lipofectamine 3000. The transfected cells were sorted for Venus expressing cells the next
day. Sorted cells were plated and grown on gelatin-coated plates under dilute conditions to
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obtain individual clones. After one week, individual clones were isolated and were used for
direct cell lysis PCR using Viagen DirectPCR solution. PCR positive clones were further grown
on gelatin-coated plates and cell lysates were obtained for Western blot analysis. Homozygous
and heterozygous Halo-tagged TBP cell lines were generated, one homozygous of which was
further tested by teratoma assay and was performed by Applied Stem Cell. We also generated
homozygous mAID-TBP cell lines, one of which (C94) was further used to endogenously knock-
in HaloTag to the Rpb1 locus, the largest subunit of RNA Polymerase II (C64 cell line). All
primers and guide RNAs used to generate knock-ins are listed in Supplemental Table 1.
Live cell and fixed sample imaging
Live-cell imaging experiments including FRAP were performed on cells grown on gelatin-coated
glass bottom microwell dishes (MatTek #P35G-1.5–14-C) and labeled with the Halo-ligand dye
JF549 at 100 nM concentration for 30 minutes. To remove unbound ligand, cells were washed
3x with fresh media for 5 minutes each. Epi-fluorescence time lapse imaging was performed on
Nikon Biostation IM-Q equipped with a 40x/0.8 NA objective, temperature, humidity and CO2
control, and an external mercury illuminator. Images were collected every 2 minutes for 12 hr.
Confocal live-cell imaging was performed using a Zeiss LSM 710 confocal microscope equipped
with temperature and CO2 control. For fixed imaging, labeled cells were fixed with 4% PFA for
10 minutes in room temperature and were washed with 1x PBS prior to imaging. Standard
immunofluorescence was performed on labeled cells using 4% PFA. Quantification of
chromosome enrichment was performed using Fiji.
FRAP
FRAP was performed on Zeiss LSM 710 confocal microscope with a 40x/1.3 NA oil-immersion
objective and a 561 nm laser as previously described (Teves et al., 2016). Bleaching was
performed using 100% laser power and images were collected at 1 Hz for the indicated time.
FRAP data analysis was performed as previously described (Hansen et al., 2017). For each cell
line, we collected 10 cells for technical replicates in one experiment, which was repeated for a
total of three biological replicates (30 cells total).
Single molecule imaging – Slow tracking
Cells were labeled with JF549 at 10 pM for 30 minutes, and washed 3x with fresh media for 5
minutes each to remove unbound ligand. Cells were imaged in ESC media without phenol-red.
A total of 600 frames were collected for imaging experiments at 500 ms frame rate (2 Hz) and
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were repeated 3x for biological replicates, with each experiment consisting of 10 cells for
technical replicates each. Data are represented as mean over experimental replicates (30 cells
total) ± SEM. Imaging experiments were conducted as described previously (Teves et al., 2016)
on a custom-built Nikon TI microscope equipped with a 100x/NA 1.49 oil-immersion TIRF
objective (Nikon apochromat CFI Apo SR TIRF 100x Oil), EM-CCD camera (Andor iXon Ultra
897), a perfect focusing system (Nikon) and a motorized mirror to achieve HiLo-illumination
(Tokunaga et al., 2008). Bound molecules were identified using SLIMfast as previously
described (Teves et al., 2016). The length of each bound trajectory, corresponding to the time
before unbinding or photobleaching, was determined and used to generate a survival curve
(fraction still bound) as a function of time. A two-exponential function was then fitted to the
survival curve, and the residence time was determined as previously described (Teves et al.,
2016). The apparent half-life in seconds of bound Halo-Pol II was calculated by dividing the
natural log of 2 with the photobleaching-corrected koff (ln2/koff) extracted from the two-
exponential function fitting. Photobleaching correction is performed by subtracting the apparent
koff of H2B-Halo from the apparent koff of Pol II samples as previously described (Hansen et al.,
2017; Teves et al., 2016).
Single molecule imaging – Fast tracking
Cells were labeled with photo-activatable PA-JF549 at 25 nM for 30 minutes and washed 3x
with fresh media for 5 minutes each to remove unbound ligand. Cells were imaged in ESC
media without phenol-red. A total of 20,000 frames were collected for at 7.5 ms frame rate (133
Hz) and were repeated 3x for biological replicates, with each experiment consisting of eight cells
of technical replicates. Data are represented as mean over experimental replicates (24 cells
total) ± standard error of means. Single molecules were localized and tracked using SLIMfast, a
custom-written MATLAB implementation of the MTT algorithm (Sergé et al., 2008), using the
following algorithm settings: Localization error: 10−6.25; deflation loops: 0; Blinking (frames); 1;
maximum number of competitors: 3; maximal expected diffusion constant (µm2/s): 20. The
fraction of bound molecules was determined as previously described using the following fit
paramerters: TimeGap, 7.477; Gaps Allowed, 1; Jumps to consider, 4; Model fit type, CDF;
Localization error, 0.045 (Hansen et al., 2017, 2018; Teves et al., 2016) using Spot-On (source
code freely available at https://gitlab.com/tjian-darzacq-lab/spot-on-matlab ). The general
statistics for image analysis (number of detections, number of total trajectories, and number of
trajectories ≥3) for all spaSPT data are listed in Supplemental Table 2.
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ChIP-seq
ChIP-seq was performed as described previously (Skene and Henikoff, 2015). Briefly, mouse
ES cells (JM8.N4) were cross-linked using 1% formaldehyde for 5 minutes at room temperature
and washed with PBS before quenching with 125mM Glycine in PBS for 5 minutes. Cells were
scraped, collected by centrifugation, and resuspended in 200 µL of Lysis buffer (1% SDS,
10mM EDTA, 50 mM Tris-HCl (pH 8.1), protease inhibitors) for 10 minutes on ice. Lysates were
diluted 10-fold in cold ChIP dilution buffer (1% Triton X-100, 20 mM Tris-HCl (pH 8.1), 2mM
EDTA, 150 mM NaCl, 5 mM CaCl2). MNase (5 µL of 0.2 U/µL stock) was added to the lysate
and samples were incubated at 37C for 15 minutes. Digested was quenched by adding EDTA
(final concentration of 10 mM) and EGTA (final concentration 20 mM). Samples were sonicated
using Branson digital sonifier at 40 seconds on time at 30% power with 2.5 seconds on and 5
seconds off cycles. Lysates were cleared by centrifugation and used as input for ChIP by adding
a-TBP antibody (Abcam #ab51841) and incubating overnight. Protein-G magnetic beads were
used to immuno-capture bound fragments, which were then washed as described previously
(Skene and Henikoff, 2015), and DNA was purified by ethanol extraction. Two replicates were
performed, and each sample and replicate was sequenced using one lane of Illumina Hi-Seq
2500 for 50 bp paired-end reads. Reads were mapped on mm10 genome build using Bowtie2
with the following parameters: --no-unal --local --very-sensitive-local --no-discordant --no-mixed
--contain --overlap --dovetail --phred33 –I 10 –X 2000. Downstream analyses were performed
using DeepTools suite (Ramírez et al., 2016). Data is deposited in GEO under the accession
number XXX.
Chr-RNA-seq
Chromatin associated nascent RNA was extracted as previously described (Teves and Henikoff,
2011). Briefly, 10 million celsl were collected for each sample as described in Figure 6C. Each
sample was washed with ice-cold PBS and lysed with 800 µL of Buffer A (10 mM HEPES, pH
7.9, 10 mM KCl, 1.5 mM MgCl2, 0.34 M Sucrose, 10% Glycerol, 1 mM DTT, 0.1% Triton X-100,
protease inhibitors) as described. Nuclei were subjected to consecutive biochemical
fractionation with incubations for 15 minutes each with centrifugation and collection in between
each fractionation. Nuclei were incubated 3 times for 15 minutes with Buffer B (9 mM EDTA, 20
mM EGTA, 1 mM DTT, 0.1% Triton X-100, protease inhibitors), then 2 times for 15 minutes
each with Buffer B+ (20 mM EDTA, 20 mM EGTA, 2mM spermine, 5 mM spermidine, 1 mM
DTT, 0.1% Triton X-100, protease inhibitors). Following fractionation, RNA from the insoluble
chromatin was extracted with Trizol and prepared for sequencing as previously described
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(Teves and Henikoff, 2011). Sequencing was performed on one lane of Hi-Seq 4000 with 50 bp
single-end reads.
Chr-RNA-seq analysis
The sequenced reads were mapped to either the mm10 genome build or ERCC92 build for the
spike-in controls using Tophat with the following parameters: library-type = fr-firststrand, b2-
very-sensitive, no-coverage-search. The mapped reads were de-duplicated using the samtools
rmdup function and then scaled using the scaling index calculated from the total number of
reads that mapped to the ERCC92 build. The scaling equation is 1000/# of de-duplicated
ERCC-mapped reads (Supplemental Table 3). Bigwig files were generated using DeepTools
suite bamCoverage function, and reads were extended for 200 bp. Intronic transcripts per
million (TPM) counts for each gene were calculated using Bioconductor R, which were then
inputted for principal component analysis. Scatter plots were generated using R ggplots
package. TSS plots, heatmaps, and k-means clustering analyses were generated with
combined replicates using DeepTools suite (Ramírez et al., 2016). Data is deposited in GEO
under the accession number XXX.
Figure Legends
Figure 1. Endogenous TBP associates with mitotic chromosomes. A. Previous ATAC-seq data
(Teves et al., 2016) examined for TSS analysis. Heatmaps for all genes centered at the TSS
(top) and aggregate plots of global average signal (bottom) surrounding the TSSs of all genes
for reads under 100 bp (left), and for mononucleosome-sized fragments (right). For
mononucleosome-sized fragments (180-250 bp), the center 3-bp nucleotide corresponding to
the central dyad of the nucleosome is mapped, resulting in narrower peaks B. Western blot
analysis of whole cell extracts of clones derived from endogenous tagging of TBP to insert the
HaloTag. C. Time-lapse live-cell imaging of C41 HaloTBP cells stably expressing H2B-GFP as
cells undergo mitosis. D. Live imaging versus fixed immunofluorescence for cells over-
expressing Halo-TBP or the endogenous C41 Halo-TBP knock-in. E. Chromosome enrichment
levels for either the over-expressing Halo-TBP cells under live or fixed conditions, or the C41
Halo-TBP knock-in cells under live or fixed conditions. n = 40 cells. Data are represented as
mean ± SEM.
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Figure 2. TBP dynamics within live cells. A. Jump length histogram measured in displacements
(µm) after 3 consecutive frames (Dt = 22.5 ms) during spaSPT for cells in interphase (blue) or in
mitosis (red). B. Cumulative distribution function of displacements after 3 frames (Dt = 22.5 ms)
during spaSPT for cells in interphase (blue) or in mitosis (red). C. Depiction of different states
for the 2-state or the 3-state kinetic model. For the 2-state model, the molecules switch from fast
diffusing mode to bound states. In the 3-state model, the freely diffusing molecules can be
divided into two categories, fast and slow, which can switch to a DNA-bound state. D. Dwell
time histogram of the fraction of endogenously-tagged Halo-TBP molecules remaining bound for
interphase (blue) and mitotic (red) cells. E. Quantification of the residence time of Halo-TBP in
interphase (blue) and mitotic (red) cells. n = 30 cells. F. Quantification of fluorescence recovery
at the bleach spot for the indicated Halo-tagged construct in interphase and mitosis. n = 30
cells. G. Data from F, normalized for bleach depth. Data are represented as mean ± SEM.
Figure 3. TBP maintains binding to promoters of active genes during mitosis. A. Genome
browser profiles for TBP ChIP-seq replicates in asynchronous and mitotic cells and the
corresponding IgG ChIP control. B. Heatmaps of the log2 ratio of ChIP over the input signal
surrounding the TSS of all genes, arranged by decreasing gene expression for asynchronous
and mitotic samples. C. Average ChIP-seq read density for all TSS and surrounding regions for
asynchronous (blue) and mitotic (red) samples and corresponding IgG controls (grays). D. Unbiased k-means clustering of data from B with k = 6. Clusters are grouped into 3 groups
depending on changes in signal. E. Gene Ontology term analysis of genes in Group 1 and
Group 3 from D. Numbers correspond to the number of genes within the group that is labeled
with the specific GO term.
Figure 4. Drug-inducible degradation of endogenous TBP. A. Schematic for mechanism of
auxin-inducible degradation. Ub, ubiquitin. B. Western blot analysis for time-course of Auxin
(IAA)-dependent degradation of WT cells or cells with the endogenous knock-in of the mAID to
the TBP locus. C. Immunofluorescence using a-TBP of cells with endogenous mAID-TBP and
stably expressing H2B-GFP without IAA (top) or after 6 hours of IAA treatment (bottom). D.
Western blot analysis of wild-type (WT) ES cells or Halo-Pol II knock-in (C64) using a-Flag to
detect the Halo-Flag knock-in and a-N-20, an antibody against the N-terminal of Pol II, to detect
all Pol II levels. The unphosphorylated and phosphorylated bands for endogenous and Halo-Pol
II are marked. E. Live imaging of Halo-Pol II showing nuclear localization as marked with H2B-
GFP. F. Cumulative distribution function (CDF) of Halo-Pol II displacements for three
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consecutive frames (Dt = 22.5 ms) for untreated cells, or cells treated with 30-60 min of
Flavopiridol or Triptolide. G. A 3-state model used to fit the CDF in F and the fraction of bound
Halo-Pol II was extracted and plotted for each condition. UT, untreated. F, Flavopiridol. T,
Triptolide. n = 30 cells and data are represented as mean ± SEM.
Figure 5. TBP-dependent dynamics of Pol II in live cells. A. Cumulative distribution function of
displacements after 3 frames (Dt = 22.5 ms) during spaSPT of endogenous Halo-Pol II for cells
in interphase (left) or in mitosis (right) either with or without IAA treatment (TBP degradation). B.
Dwell time histogram of the fraction of endogenously-tagged Halo-Pol II molecules remaining
bound for interphase (blues) and mitotic (reds) cells either with or without IAA treatment, as
indicated in legend. C. Quantification of the apparent half-life (see Methods) in seconds of Halo-
Pol II in interphase (blues) and mitotic (reds) cells. n = 30 cells. D. Quantification of
fluorescence recovery at the bleach spot for Halo-Pol II in interphase (blues) and mitosis (reds),
either with or without IAA treatment. n = 30 cells. E. from D, the average time to reach 90%
recovery for Halo-Pol II in interphase (blues) or mitosis (reds), either with or without IAA
treatment. Data are represented as mean ± SEM.
Figure 6. TBP recruits Pol II during mitosis. A. The fraction of bound Halo-Pol II molecules as a
function of time (t = 0, release from DMSO/IAA treatment) under no IAA (WT conditions) or after
6 hours of IAA treatment (teal) for interphase cells. B. Same as A, but for mitotic cells. C.
Schematic of time course regimen for extracting chromatin-associated nascent RNA.
Asynchronous cells are treated with DMSO or IAA for 6 hours prior to chromatin-associated
nascent RNA extraction (not depicted). For other samples, cells are synchronized with
Nocodazole for 6 hours, and treated with DMSO (untreated) or IAA (TBP-degraded) during
Nocodazole synchronization. For mitotic samples (M), cells are immediately collected. For time
course after mitosis, synchronized M cells (untreated or TBP-degraded) are replaced into fresh
media to release from mitotic arrest and TBP degradation and are collected either after 30
minutes (M30) or 60 minutes (M60) following fresh media resuspension. D. Extracted
chromatin-associated nascent RNA were sequenced in strand-specific manner, and the sense
(blue) and anti-sense (red) reads are plotted for Gapdh (left) and Nanog (right) loci for all
corresponding samples. E. Genome-wide average plots for all TSS and surrounding regions for
sense (blue) and anti-sense (red) reads for each indicated untreated sample, and the
corresponding heatmaps for all reads (bottom). F. Same as E but for TBP-degraded samples.
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25
Figure 7. TBP promotes efficient reaction of transcription following mitosis. A. The log2 ratio of
M30 and M60 reads relative to M reads were calculated for untreated and TBP-degraded
samples (M30/M and M60/M, respectively). The M30/M samples were clustered using k-means
clustering with k = 3, and the rest of the samples are ordered by this clustering, and average
plots surrounding the TSS are shown for each cluster. B. Heat map analysis of each cluster for
each sample in A. C. GO term analysis for genes present in cluster 1 (top) and cluster 3
(bottom). Numbers correspond to the number of genes within the custer that is labeled with the
specific GO term.
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LiveFixed
H2B-GFP HaloTBP OE H2B-GFP HaloTBP KI HaloTBP OE
Chr
Enr
ichm
ent
-0.3
-0.2
-0.1
0.0
0.1
0.2
0.3
Live
Fixe
d
Figure 1
A B C
D
TBPEndogenous
Halo-taggedC19 C29 C41 WT
Endogenous Halo-tagging of TBP
H2B-GFP
HaloTBP KI
HaloTBP C41 H2B-GFP
HaloTBP C41
0’
2’
4’
6’
12’
14’
E
-2.0 TSS 2.0Kb -2.0 TSS 2.0Kb0
20
40
60
-2.0 TSS 2.0Kb -2.0 TSS 2.0Kb0.0
1.0
2.0
3.0
Under 100 bp MonoNucleosome reads
-2.0 TSS 2.0Kb
10
20
30
40
Asynch Mitosis
-2.0 TSS 2.0Kb
0.5
1.0
1.5
Asynch Mitosis
AsynchMitosis
F
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A
B
Figure 2
Res
iden
ce T
ime
(s)
0
30
60
90
120
bound slow
fast
bound
k*ONkOFF
Dis
plac
emen
t CD
F
Displacement (µm)
Δτ = 22.5 ms
0 0.2 0.4 0.6 0.8 10
0.2
0.4
0.6
0.8
1
IntMit
Δτ = 22.5 ms
0 0.2 0.4 0.6 0.8 1Displacement (µm)
Pro
babi
lity
1 10 1000.001
0.01
0.1
1
Dwell time (s)
% M
olec
ules
bou
ndIntMit
Time (seconds)-20 0 20 40 60 80 100 120 140 160
FRA
P re
cove
ry
0
0.2
0.4
0.6
0.8
1
H2B-Halo InterphaseHalo-3xNLS InterphaseHalo-TBP InterphaseHalo-TBP Mitosis
Time (seconds)-20 0 20 40 60 80 100 120 140 160
0
0.2
0.4
0.6
0.8
1
FRA
P re
cove
ry
C
D E
F G
fast
2-State Model 3-State Model
Int Mit
Interphase
Mitosis
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Hs6st1 Arid5a Actr1b Cnga3 Coa5 Tsga10 Eif5b
10
010
010
010
010
010
0
Asy
nch
Mito
sis
Rep 1
Rep 2
IgG
Rep 1
Rep 2
IgG
0
20
40
-2 kb TSS 2 kb
AsynchMitosisA IgGM IgG
Nor
mal
ized
Cou
nts
A
B D
Figure 3
1000 kb
Asynchronous Mitosis
-2 kb TSS 2 kb -2 kb TSS 2 kb
1.0
0.5
0
-0.5
-1.0
Log 2(C
hIP
/Inpu
t) - D
ecre
asin
g ge
ne e
xpre
ssio
n
-2 kb TSS 2 kb -2 kb TSS 2 kb
Asynchronous Mitosis
Gro
up 1
Gro
up 2
Gro
up 3
0 2 4 6 8 10
Homology directed repairMicrotubule-based processesG1/S transition of mitotic cell cycleCell CycleMitotic cell cycle phase transition
0 5 10 15
Membrane traffickingCell divisionReg. of cellular catabolic processMetabolism of RNACell Cycle
Gro
up 1
Gro
up 3
-log10(P-value)
C E142
14768
14254
134137
145112120
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0 6 24 0 6 24 IAA (hr)
mAID-TBP
endogenous
WT mAID-TBPA B
Figure 4
Auxin (IAA)
mAID-TBP
Ub
CH2B-GFP mAID-TBP Merge
- IA
A +
IAA
D
E
0 0.2 0.4 0.6 0.8 1
Dis
plac
emen
t CD
F
0
0.1
0.2
0.3
0.4
0.5
0.6
0.7
0.8
0.9
1
Triptolide (T)Flavopiridol (F)Untreated (UT)
Δτ = 22.5 ms
0
10
20
30
% B
ound
Mol
ecul
es
Displacement (µm)
F
UT F T
G
WT C64 WT C64
Flag N-20
EndogenousHalo-Pol II
H2B-GFP Halo-Pol II
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0 0.2 0.4 0.6 0.8 1
Dis
plac
emen
t CD
F
0
0.2
0.4
0.6
0.8
1
- IAA
0 0.2 0.4 0.6 0.8 1
IntInt IAAMitMit IAA
1 10 1000.001
0.01
0.1
1
Dwell time (s)
Frac
tion
rem
aini
ng b
ound
Halo-Pol II Interphase Halo-Pol II Mitosis
+ IAA- IAA+ IAA
A
B
Figure 5
Displacement (µm) Displacement (µm)
Time (s)-20 0 20 40 60 80 100 120 140 160
FRA
P re
cove
ry
0.4
0.5
0.6
0.7
0.8
0.9
1
IntInt IAAMitMit IAA
0
2
4
6
150
200
T90%
Rec
over
y (s
)
C
Δτ = 22.5 ms Δτ = 22.5 ms
D E
App
aren
t Hal
f-Life
(s)
0
10
20
30
– IAA – IAAInt Mit
– IAA – IAAInt Mit
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Iffo1 Gapdh
1 kb
Nanog
1 kb170
-50
170
-50
170
-50
170
-50
170
-50
170
-50
170
-50
170
-50
100
-20100
-20100
-20100
-20100
-20100
-20100
-20100
-20
Sense
Antisense
A
M
M30
M60
A
M
M30
M60
A
M
M30
M60
A
M
M30
M60
Untreated
TBP degraded
Untreated
TBP degraded
-5
0
15 A M M30 M60
-5
0
15
-2kb TSS 2kb
A
-2kb TSS 2kb
M
-2kb TSS 2kb
M30
-2kb TSS 2kb
M60
-6 hr 0 0.5 1 hr
+/- Noc (Untreated)+/- IAA (TBP-degraded)
Synchronization
Collect M cells
Fresh media
Collect M30 cells
Collect M60 cells
Time (m)Time (m)
A
C
E
D
0 15 30 45 600.15
0.30
0.45– IAA + IAA
0 15 30 45 600.15
0.30
0.45
+ IAA
Frac
tion
boun
d
Figure 6
B
Sense
Antisense
– IAA
-2.0 TSS 2.0Kb -2.0 TSS 2.0Kb -2.0 TSS 2.0Kb -2.0 TSS 2.0Kb
5
10
15
20
25
30
35
40
0
10
20
30
40
50
-2.0 TSS 2.0Kb -2.0 TSS 2.0Kb -2.0 TSS 2.0Kb -2.0 TSS 2.0Kb
F
Interphase Mitosis
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-2kb TSS 2kb -2kb TSS 2kb -2kb TSS 2kb -2kb TSS 2kb
Cluster 1Cluster 2Cluster 3
M30/M M60/M M30/M M60/MUntreated TBP degraded
Chromosome segregationDNA ReplicationAutophagyChromatin organizationRegulation of chromosome organizationRegulation of DNA metabolic processTranscription factor activityCell CycleDNA RepairMetabolism of RNA
0 20 40 60 80
-log10(P-value)
Cluster 1
Cluster 3
A
C283
181201
195130
109204145105116
0 2 4 6 8 10
Multicellular organism developmentCellular component disassemblyMorphogenesis of epitheliumPositive regulation of transferase activityWnt signaling pathwayChromatin organizationCell morphogenesis in differentiationCell projection assemblyRegulation of GTPase activityMicrotubule cytoskeleton organiztion99
96107
11913291
11895
100561
clus
ter_
1cl
uste
r_2
-2.0 TSS 2.0Kbgene distance (bp)
clus
ter_
3
-2.0 TSS 2.0Kbgene distance (bp)
-2.0 TSS 2.0Kbgene distance (bp)
-2.0 TSS 2.0Kbgene distance (bp)
−1.0
−0.5
0.0
0.5
1.0
1.5
M30/M M60/M M30/M M60/MUntreated TBP degradedB
Figure 7
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Fraction Bound
Fraction in slow 3D
Fraction in fast 3D
Apparent Dslow (μm2/s)
Apparent Dfast (μm2/s)
TBP Int 2-state TBP Mit2-state
TBP Int3-state
TBP Mit3-state
34.6%
18.6%
65.4%
81.4%
3.184
2.439
Table 1. TBP Nuclear Diffusion Paramerters.
24.8%
12.3%
37.2%
46.5%
38.0%
41.2%
1.407
1.261
6.354
6.364
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Fraction Bound
Fraction in complex
Fraction in 3D diffusion
Apparent Dslow (μm2/s)
Apparent Dfast (μm2/s)
Table 2. Pol II Nuclear Diffusion Paramerters.
Pol II Int
Pol II Int + IAA
Pol II Mit
Pol II Mit+ IAA
22.4%
16.1%
12.1%
10.8%
45.6%
46.6%
52.9%
55.6%
32.0%
37.3%
35.0%
33.7%
1.430
1.536
1.115
1.066
6.480
6.876
6.639
7.429
Pol II Int
Pol II Int + IAA
Pol II Mit
Pol II Mit+ IAA
2-st
ate
mod
el3-
stat
e m
odel
29.3%
19.5%
17.6%
15.1%
70.7%
80.5%
82.4%
84.9%
2.439
2.632
1.798
1.545
.CC-BY-NC 4.0 International licensecertified by peer review) is the author/funder. It is made available under aThe copyright holder for this preprint (which was notthis version posted January 31, 2018. . https://doi.org/10.1101/257451doi: bioRxiv preprint